Barcoding of Chironomidae (Diptera) Global Fresh Water ......The Chironomidae are the only free-living (non-parasitic) holometabolous insect extant on every continent, including Antarctica,

5/14/2019 2019 Stockholm National Paper 2 - Google Docs

https://docs.google.com/document/d/117or8f6OcEMlj5wtGSII_lWN--ucQiM9IK7nPB05ET0/edit 1/21

Entry into the Stockholm Junior Water Prize 2019

A Novel Method of Monitoring the Health of our

Global Fresh Water Supply using DNA

Barcoding of Chironomidae (Diptera)

Sonja Michaluk

New Jersey



I. Abstract: It is forecast that 66% of our population will experience water scarcity within a decade,

leaving us more dependent on surface water for drinking. [14] This requires more filtration infrastructure,

and monitoring of surface water sources. Current methods rely on expensive and technically challenging

manual identification of biological samples. Macroinvertebrates spend their larval lives within a small

area of water, showing cumulative effects of habitat alteration and pollutants that chemical testing and

field sensors do not. [9] Molecular methods enhance biomonitoring programs. This project explores

deoxyribonucleic acid (DNA) barcoding, to measure waterway health with larval Chironomidae (order

Diptera), the most widespread macroinvertebrate family. [4] Their complex taxonomy makes manual

morphological identification difficult. A statistical sampling plan was designed that represents variation

in geological, ecological, and land use factors. Fou r m ethods of isolation and amplification were

compared. Statistical analysis shows DNA Barcoding of Chironomidae results in more accurate and

precise waterway health data, adding significant value for monitoring scarce water resources. The

learnings from these data are being applied building microbiology capability at a non-profit water study

institute.

II. Table of Contents: 1. Introduction - p2

2. Materials and Methods - p5

3. Results - p7

4. Discussion - p14

5. Conclusions - p18

6. References - p19

7. Bibliography - p20

III. Key Words: Public Water, Chironomidae, Water Scarcity, DNA Barcoding, Surface Water, Water

Monitoring, Bioassessment, Nonpoint Source Pollution, Macroinvertebrate, COI (cytochrome c oxidase

subunit 1)

IV. Abbreviations and Acronyms: COI: Cytochrome c oxidase subunit 1

NJDEP: New Jersey Department of Environmental Protection

PCR: Polymerase chain reaction

V. Acknowledgements: This effort was designed and conducted by the author. Appreciation to Karen

Lucci of Hopewell Valley Central High School for guidance on phylogenetic tree analysis. Based on

previous training and experience, Cold Spring Harbor Laboratory graciously allowed open access to

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microbiology labs and equipment to conduct independent experimentation. Special appreciation to Dr.

Cristina Fernandez for DNA Barcoding principles. Sample preparation, DNA extraction,

macroinvertebrate identification and chemical analysis was performed in home laboratory underwritten

by funding awarded for prior research. Additional thanks to Erin Stretz, Dr. Steve Tuorto, and Jim

Waltman from The Watershed Institute for internships and opportunities to learn aquatic entomology and

chemical environmental monitoring; Dr. Patricia Shanley for guidance on policy and advocacy;

Lawrenceville Summer Scholars for robotics and programming.

VI. Biography: My independent research focuses on how environmental data can be gathered and used

to inform decision making in terms of how and when we develop our natural and water resources. I have

been a member of the Society for Freshwater Science since 2014, and I have presented data at their 2015

Mid-Atlantic Chapter meeting at the Academy of Natural Sciences in Philadelphia, and the 2017 Annual

Conference in Raleigh, North Carolina. Additionally, I have presented at the Environmental Protection

Agency (EPA), for receiving a Presidential Award, National Geographic Society in Washington, D.C.,

as well as New York Academy of Sciences Bicentennial celebration, New York, NY (2017).

Massachusetts Institute of Technology (MIT) named a minor planet in my honor. Through chemical and

biological stream assessment (certified for 8 years), I have been monitoring the health of our local

waterways as an active member of a StreamWatch volunteer program since 2011. Encyclopedia

Britannica published my definition of “macroinvertebrate.” I was the featured speaker and Watershed

Hero at The Alliance for Watershed Education River Days 2017 & the East Coast Greenway River Days

Kick-Off at Fairmount Water Works, Philadelphia.

My research, data collection, and advocacy have led to environmental improvements: data

submission to the New Jersey Department of Environmental Protection (NJDEP) and modifications to a

pipeline construction project that minimized impact to streams, 20 acres of ecologically critical forest

and wetland being preserved as open space, providing a critical east-west wildlife habitat corridor. My

efforts to locate and document the southernmost population of a threatened amphibian species support a

current proposal for categorization of a special wetland habitat as a C1 Stream by the NJDEP.

1. Introduction : Parts of the world are abundant with fresh water, but 2.7 billion people (about 40% of

our population) experience water scarcity at least one month a year. [14] This is expected to grow to

two-thirds of the world’s population within a decade (Falkenmark Water Stress Indicator) as population

and water usage increase. [14] Less than 1% of the world’s water is accessible as a public water source. [3]

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Water scarcity affects every continent and was listed in 2015 by the World Economic Forum as the

largest global risk in terms of potential impact over the next decade. [13][6]

As water scarcity increases, we become more and more dependant on surface water for drinking,

therefore require more filtration infrastructure, and more monitoring of surface water sources. Currently

63% of public water (serving a population of 169 million) in the USA is from surface water. [10] Wetlands

provide surface water filtration, however more than half the world’s wetlands have disappeared. [14]

New York City makes use of wetlands as a natural water filtration resource for their public water. Over

1,000,000 acres of protected land in the Catskill/Delaware watersheds provide natural filtration for 90%

of New York City’s population of 8.5 million. [11] New York is one of only five cities that can rely on

simpler natural filtration for public water. [11] The New York City Land Acquisition Program purchased or

protected over 130,000 acres since 1997 and restricts development. [8] A dedicated police force of more

than 200 members guards the health of the wetlands and prevents illegal dumping. [12]

Measures of taxa richness and relative abundance provide valuable information on trends in

ecosystem health. Macroinvertebrates provide a logical choice because they can be seen with the naked

eye and spend their larval lives in a small area of water and therefore show the cumulative effects of

habitat alteration, contaminants, and pollutants. Additionally macroinvertebrates play a significant part

of the food web, preyed upon by fish, birds, reptiles, and amphibians. Current waterway assessment

methods are based on a procedure defined and popularized and standardized by Hilsenhoff [7] in 1977: a

100 organism sub-sample is obtained from a Stratified Random Sample taken in the field. Organisms are

identified to the lowest practical taxonomic level with a microscope and taxonomic keys. [7][9]

These current methods of surface water monitoring can be expensive and technically

challenging, relying on manual identification of biological macroinvertebrate samples. Additionally

macroinvertebrates are relatively easy to identify to family level manually by morphology, however

genus and species level identification is exponentially more complex. Highly detailed genus and species

level data is more accurate and precise but difficult to obtain due to cost, specimen condition, incomplete

taxonomic knowledge, poor taxonomic keys, and lack of trained taxonomists. Error rates of genus and

species in samples identified by professional taxonomists have been found to be as high as 65%. [4]

Molecular methods, such as deoxyribonucleic acid (DNA) barcoding from a region of the mitochondrial

gene COI (cytochrome c oxidase subunit 1), have begun to enhance biomonitoring programs. DNA

Barcoding offers the promise of a more rapid, accurate (less human error), and precise (species level)

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identification of macroinvertebrate taxa. This is important to obtain accurate environmental assessments.

DNA Barcoding overcomes limitations of manual taxonomic identification and significantly improves

the statistical power of bioassessment tools. [15] Taxonomic identification to family level by volunteers is

widely used for citizen science programs and broad data gathering. Many studies have explored the

potential of DNA Barcoding for bioassessment, and the increased precision and statistical power

provided by genus and species level identification. This effort creates a methodology that allows DNA

Barcoding to be integrated into existing water monitoring programs. This project aims to enhance citizen

science environmental monitoring programs with a DNA Barcoding methodology and capability in

order to improve accuracy, precision, and statistical power of results.

Figure 1. DNA Barcoding

resolves even cryptic species

that are morphologically

indistinguishable

This project explores the potential of using DNA Barcoding to measure waterway health with the

larval non-biting midge Chironomidae (order Diptera). Chironomidae are versatile macroinvertebrates

and a common denominator among most aquatic sites. [4] They occupy many important parts of food

webs, and includes all functional feeding groups: collector/gatherers, shredders, scrapers, filter-feeders,

and predators. [4] They have a holometabolous, or complete metamorphosis, life cycle with; egg, larva,

pupa, and adult. The Chironomidae are the only free-living (non-parasitic) holometabolous insect extant

on every continent, including Antarctica, and in a great range of altitudes. [4] They have been found 5600

m above sea level on glaciers in Nepal, and 1360 meters below the surface of freshwater Lake Baikal in

Russia. This project is concerned with the larval form, which in some species occurs in water films a

millimeter thick, and in others dwells in arid regions and can tolerate drought (one even survived 18

months in the vacuum of space). Other larvae are found in glacial meltwater just above freezing, and

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there are even Chironomidae in hot springs over 40°C. There are fully marine species, and some have

even been found in algae on sea turtle shells. Some Chironomid larvae have hemoglobin which allow

them to absorb oxygen from and tolerate low-oxygen waters that other macroinvertebrates cannot

survive. Due to their reddish color they are commonly called bloodworms. Unfortunately for citizen

scientists, Chironomidae have complex taxonomy that makes manual morphological identification to

genus and species level extremely difficult. The Hilsenhoff Family Tolerance Value for Chironomids is

6. This is an average of the Genera Tolerance Values which have been shown to range greatly (e.g. from

2 to 10 for the genera sampled here). Since they are difficult to identify morphologically, DNA

Barcoding adds great value, additionally unlike some other macroinvertebrates they lack inhibitors that

impede amplification using the silica resin isolation method and polymerase chain reaction (PCR)

primer beads.

This research hypothesizes that a novel DNA Barcoding process utilizing Chironomidae

(Diptera) will compare favorably to standard methods of monitoring surface water sources. The purpose

is to contribute an improved method of bioassessment to aid in preservation of our freshwater resources.

In phase 1, method development was explored. The independent variables were DNA extraction

methods and primers used. The dependent variable was the percent amplification of samples. The

control was the DNA ladder.

In phase 2, The Chironomidae were explored as an index of waterway health. The independent

variables were the sample sites, varying freshwater bodies with a statistically planned variety of

geological, ecological, and anthropogenic factors. The dependent variables were the genera and species

present. The positive control is a known healthy location (per statistical data) and manual identification.

The negative control is known unhealthy location.

The research questions explored here support creation of a microbiology lab at a non-profit water

study institute that supplements their existing citizen science water monitoring programs. 1) Can DNA

Barcoding be used as a means of monitoring surface water sources? 2) How do Chironomidae genera

and species vary in response to variation in geological, ecological, and land use factors? 3) How do

Chironomidae genera and species vary in response to nutrient pollution? 4) Will this project add new

species to the Chironomidae data sets in genetic sequence databases used by the scientific community?

5) What is the effect of different methods of PCR on the amplification of Chironomidae DNA?

2. Materials and Methods:

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2.1 Risk and Safety: These procedures involve use of ethanol, a Lamotte Water Quality test kit, and

microliter amounts of DNA isolation, PCR amplification, and gel electrophoresis reagents. Material

Safety Data Sheets (MSDS) sheets were reviewed. Personal protective equipment was used to protect

against risk of chemical exposure. Waste liquid was collected and given to Clean Harbors, a company

specializing in hazardous waste disposal. Training was completed and up to date for equipment,

chemicals, and taxonomic identification.

2.2 Procedures: The following methods of DNA isolation were selected (Rapid DNA Isolation,

PowerSoil Isolation Method (Metabarcoding), Silica Resin Isolation). Research showed these to be more

likely to work for macroinvertebrates and they are fairly easy and economical for real world use.

A statistical sampling plan was designed to represent variation in geological, ecological, and land use

factors. Sample sites were chosen according to a statistical sampling plan to capture a variety of

geological, ecological, and anthropogenic factors: high gradient vs coastal plain, stream vs. pond,

healthy ecosystem vs. unhealthy ecosystem.

2.3 Water Quality Chemical Analysis: Water quality chemical analysis certifications relevant to this

project were up to date. Chemical sampling was performed with LaMotte water test kit and procedure.

Nitrates, orthophosphates, dissolved oxygen, pH, and turbidity was monitored over 9 months at 13 sites.

2.4 Benthic Macroinvertebrate Sampling : Sampling was performed per NJDEP procedure. Freshwater

macroinvertebrate samples were collected with D-frame net. The percentage of net jabs taken in each

habitat type corresponded to the percentage of each habitat type’s presence in the stream reach. The

sample was stored in ethanol. Macroinvertebrates were identified, and those from the Chironomidae

family (order Diptera) were identified under a microscope and removed for DNA Barcode analysis.

Stream health was monitored over 9 months at 13 sites.

2.5 DNA Isolation Procedure : The membrane-bound organelles such as the nucleus and mitochondria

were dissolved with lysis solution. A sterile plastic pestle was used to liquify the macroinvertebrate

sample in a 1.5ml tube. Silica resin was used to bind DNA. The nucleic acids were eluted from the silica

resin with laboratory grade distilled water. Samples were stored at -20 C prior to PCR amplification.

2.6 Polymerase Chain Reaction (PCR) Amplification : Primers were selected based on sample type.

Different methods of PCR amplification were tested: Ready-To-Go PCR Beads were activated by adding

a mix of loading dye and COI primers LCO1490 and HC02198. After bead dissolves, the DNA sample

was added with micropipette. The PCR tubes was then be mixed by lightly flicking, and centrifuged for

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30 seconds at 13,400 RPM to spin the liquid to the bottom of the tube. Samples were thermal cycled

with the appropriate temperature profile programmed. NEB Taq 2X Master Mix: 10μL of loading dye

per sample was mixed with 12.5μL of NEB Taq 2X Master Mix per sample, combined in a 1.5ml tube,

and shaken gently for mixing. 2μL of sample DNA was then be added with micropipette to the

correspondly labeled PCR tubes. 23μL of the LCO1490 and HC02198 primer mix was added to each

PCR tube. The PCR tubes were then be mixed by lightly flicking, and centrifuged for 30 seconds at

13,400 RPM to spin the liquid to the bottom of the tube. Samples were then be thermal cycled with the

appropriate temperature profile programmed.

2.7 Gel Electrophoresis: Agarose gel was poured, and when it was solid it was be placed into the

electrophoresis chamber. Tris/Borate/EDTA (TBE) buffer was added. PCR samples was loaded, the gel

was run at 130V and the image were captured. Images for samples prepared with PCR Beads and with

Master Mix were used to verify DNA amplification.

2.8 Sequencing: Samples were then sent for DNA Sequencing. Bioinformatic analysis was completed

by trimming and analyzing the Chironomidae genetic sequences. The final sequences were submitted

and compared to multiple genetic sequence databases to determine the genus and species of each sample.

Software tools were programmed and developed to easily calculate biological health scores. The

appropriate index was selected (High Gradient or Coastal Plain Macroinvertebrate Index).

3. Results: DNA Barcoding overcomes limitations of manual taxonomic identification and significantly

improves the statistical power of bioassessment tools. [15] Hilsenhoff tolerance scores of the

Chironomidae genera sampled and identified using the DNA Barcoding method developed here were

used with GIS software to provide an overview of water quality.

Figure 2. Overview of waterway health

using Hilsenhoff tolerance scores of the

Chironomidae genera identified by

DNA Barcoding. [5]

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Highly detailed genus and species level data is more accurate and precise but difficult to obtain

due to cost, specimen condition, incomplete taxonomic knowledge, poor taxonomic keys, lack of trained

taxonomists.

Figure 3. The left diagram shows a taxonomic macroinvertebrate sample identified to class and family

level by a trained volunteer. The right diagram shows the sample identified to species level by DNA

Barcoding, and reveals the additional resolution provided by DNA Barcoding.

An important step to developing a methodology for use of Chironomidae in bioassessment was

comparing and evaluating molecular analysis methods. Silica resin and PCR bead successfully amplified

100% of the samples. Four approaches were evaluated, and had very different results in terms of the

percent of samples that accurately identified.

Figure 4. Summary of the

molecular analysis methods

evaluated. Silica resin and PCR

bead successfully amplified

100% of the samples.

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The Chironomidae samples showed the least undetermined nucleotides, best peak quality, and

best sequence quality. The Gammaridae also responded very well to barcoding, However the

gammaridae do not have the range of geography and biotic indices that the Chironomidae do.

Figure 5. Summary of various

taxa samples identified by DNA

Barcoding with silica resin and

PCR beads, and compares their

response to DNA Barcoding.

Phred scores were compared using two-sample t-tests (0.01 significance level). This test was selected

because the number of samples n was less than 30.

Chironomidae vs. Physidae p = 1.01 x 10 -6 indicating a statistically significant difference.

Chironomidae vs. Haliplidae p = 7.37 x 10 -8 indicating a statistically significant difference.

Chironomidae vs. Gammaridae p = .053 indicating a difference that is not significant, however

Gammaridae were not chosen due to their more limited number of species, geographic range, and

biotic index range.

The Chironomidae sampled here aligned by genera with either high gradient streams in piedmont

geology, or sandy soils and coastal plain geology. Only 13% of the genera sampled were found evenly in

both geologies.

Figure 6. Percent of Chironomidae genera based on

the surface geology they predominantly occur in.

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Nutrient pollution was compared with the weighted average Hilsenhoff scores of the Chironomidae

genera sampled at each site. The value for nutrient pollution was calculated from the average ppm of

nitrate and orthophosphate sampled at each site, which was normalized to a value between



Figure 8. Relationship between the

weighted average Hilsenhoff scores of

the Chironomidae genera sampled at

each site, and the overall historical

health based on sampling at each site.

A Bland-Altman analysis showed limits of agreement of -0.853 and 0.868 between the weighted average

tolerance values of Chironomidae genera barcoded and the standard method that uses manual taxonomic

identification by morphology. This indicates that the new method proposed here of DNA barcoding

Chironomidae is in agreement with the current standard to within 1.72 on a zero to ten health scale.

Figure 9. A Bland-Altman

analysis showed limits of

agreement of -0.853 and

0.868 between the weighted

average tolerance values of

the Chironomidae genera

barcoded and the standard

method that uses manual

taxonomic identification by

morphology.

The following phylogenetic trees were used to analyze the genetic relationships between selections of

the Chironomidae sampled with respect to site, taxa level identified, and biotic index.

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Figure 10. Phylogenetic tree

which diagrams the genetic

relationship between the

Chironomidae samples from six

sites with the most variation.

The following phylogenetic tree was used to analyze the genetic relationships between selections of the

Chironomidae sampled with respect taxa level identified (e.g. subfamily, genus, or species).

Identification down to species level indicates a match in the sequence databases. Identification to genus

or subfamily indicates gaps in the sequence database that can be filled with a widespread barcoding

initiative. The gaps could also allude to potential novel species.

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Figure 11. Phylogenetic tree which diagrams

the genetic relationship between Chironomidae

samples with the taxa level identified (e.g,

subfamily, genus, species).

The family biotic index for Chironomidae is 6. This masks an underlying variability as the genera

sampled for this study range in biotic index from 2 to 10

Figure 12. Phylogenetic tree which diagrams

the genetic relationship between Chironomidae

samples with the Hilsenhoff tolerance value for

each genera.

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4. Discussion

4.1 DNA Barcoding for Bioassessment: Highly detailed genus and species level data is more accurate

and precise but difficult to obtain due to cost, specimen condition, incomplete taxonomic knowledge,

poor taxonomic keys, lack of trained taxonomists. Error rates of genus and species in samples identified

by experts have been found to be as high as 65%. [4] This demonstrated the value of DNA Barcoding,

especially for identifying such versatile and phenotypically similar specimens as Chironomidae.

Hilsenhoff tolerance scores of the Chironomidae genera sampled and identified using the DNA

Barcoding method developed here were used with GIS software to provide a water quality overview

map. Visualizations from this project’s data were used in community land use decision making. In

addition to the value of making data readily available data to communities, it is important to note that

DNA Barcoding enables an increase in the amount and accuracy of data available for community and

land use decision making.

4.2 Comparison of Molecular Analysis Methods: An important step to developing a methodology for

use of Chironomidae in bioassessment was comparing and evaluating molecular analysis methods. Four

approaches were evaluated: eDNA Metabarcoding Extraction and eDNA Metabarcoding Primer, Rapid

Method (chromatography paper) Extraction and PCR Bead, Silica Resin Extraction and PCR Bead,

Silica Resin Extraction and MM Primer. Silica resin and PCR bead successfully amplified 100% of the

samples. This result also verified that the appropriate laboratory and field practices and techniques had

been used, and that the techniques and methods were not excessively cumbersome.

4.3 Selection of Chironomidae as a Global Common Denominator: Various macroinvertebrate

families were identified by DNA Barcoding with silica resin and PCR beads. Selecting one family to

focus on provided a natural limit that allowed effects of differences in extraction and amplification of

DNA to be minimized, for example macroinvertebrates with tough exoskeletons or shells can be more

difficult to extract DNA from, and many mollusks contain PCR inhibitors. The response of various

macroinvertebrate families to DNA Barcoding and success at identification was compared using

measures DNA sequence quality: visual analysis of electropherograms, Phred score, undetermined

nucleotides, peak quality, sequence quality. The Chironomidae were identified as the best option with

the best sequence quality as they had the best Phred score least undetermined nucleotides, best peak

quality, and best sequence quality. The Gammaridae also responded very well to barcoding, with a Phred

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score of 98% vs 99% for Chironomidae, however the gammaridae do not have the range of geography

and biotic indices that the Chironomidae do.

4.4 Chironomidae and Surface Geology Variation: The Chironomidae sampled here aligned by

genera with either high gradient streams in piedmont geology, or sandy soils and coastal plain geology.

Only 13% of the genera sampled were found evenly in both geologies.

4.5 Comparison of Genera Tolerance Values and Nutrient Pollution: This analysis compared the

relationship between the weighted average Hilsenhoff scores of the Chironomidae genera sampled at

each site and the nutrient pollution. The value for nutrient pollution was calculated from the average

ppm of nitrate and orthophosphate sampled at each site, which was normalized to a value between 0 and

10. This shows a statistically significant relationship with p



4.7 Phylogenetic Tree Analysis: Phylogenetic trees were used to analyze the genetic relationships

between selections of the Chironomidae sampled with respect to site, taxa level identified, and biotic

index. The phylogenetic tree in Figure 11 was used to analyze the genetic relationships between

selections of the Chironomidae sampled with respect taxa level identified (e.g. subfamily, genus, or

species). Identification down to species level indicates a match in the sequence databases. Identification

to genus or subfamily indicates gaps in the sequence database that can be filled with a widespread

barcoding initiative. The gaps could also allude to potential novel species. The phylogenetic tree in

Figure 12 diagrams the genetic relationship between Chironomidae samples with the Hilsenhoff

tolerance value for each genera. The Hilsenhoff family biotic index for Chironomids is 6. The genera

sampled range in Hilsenhoff Biotic index from 2 to 10.

4.8 Statistical Tools and Analysis: In Phase I, a two-sample t-test was used to compare Phred sequence

quality scores between Chironomidae and other macroinvertebrates sampled to a 0.01 significance level.

The two-sample t-test was selected because because the sample quantity n was less than 30. The

significance of 0.01 was chosen to emphasize the very low p value obtained for the Physidae and

Haliplidae.

When the Chironomidae were compared with Physidae, Haliplidae, and Gammaridae, the null

hypothesis was that the mean proportion of ideal Phred scores for chironomids would be equal to that of

Physidae. The alternative hypothesis was that the mean proportion of ideal Phred scores would be

greater for Chironomidae than, for example Physidae. Because p= 1.01 x 10 -6 and is lower than the

significance level of 0.01, the null was rejected, indicating that the Chironomidae DNA sequence quality

was significantly better than the Physidae sequence quality. For Chironomidae vs. Haliplidae p = 7.37 x

10 -8 < 0.01 indicating a statistically significant sequence quality improvement. For Chironomidae vs.

Gammaridae p = .053 indicating a difference that is not significant, however Gammaridae were not

chosen due to their more limited number of species, geographic range, and biotic index range.

In Phase II bioassessment measurement systems were compared. In order to compare waterway

ecosystem bioassessment by weighted average tolerance values of the Chironomidae genera barcoded,

and the standard method that uses manual taxonomic identification by morphology, a Bland-Altman

analysis was used. [1] The Bland-Altman test was selected as this is a common statistical tool used to

compare a new measurement method to an existing standard of measurement when a true value or

calibration standard is not available, and measurements must be made indirectly.

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Comparing two measurement systems by running a regression and calculating a correlation

coefficient r value is not sufficient to compare measurement systems, as two methods of measuring the

same value are nearly guaranteed to be correlated. Additionally, they can be correlated without being in

agreement, such as a measurement of length in inches, and in centimeters. [1] Bland-Altman analysis

determines the level of agreement between two measurement systems. This comparison showed limits of

agreement of -0.853 and 0.868 between the weighted average tolerance values of the Chironomidae

genera barcoded and the standard method that uses manual taxonomic identification by morphology.

This indicates that the new method proposed here of DNA barcoding Chironomidae is in agreement with

the current standard to within 1.72. This is a significant finding, especially considering that waterway

health data is often reported as good / fair / poor, and leads to the conclusion that the measurement

method is sensitive enough, and waterway ecosystem bioassessment by DNA Barcoding of

Chironomidae is a viable option for bioassessment globally.

Statistical power is the sensitivity of a test, or the ability of a test to find an effect if there is one

to be found, or in other words the probability that the test will correctly reject a false null hypothesis.

Statistical power = 1 – β, where β is the probability of making a Type II error. (alpha α is the probability

of making a Type I error.) Statistical power is an function of the sample size, alpha, and effect size.

Increasing the sample size increases statistical power, but there is typically a cost or challenge to

obtaining more samples. Increasing alpha also increases statistical power, however this merely

exchanges this risk of a Type II error (β-risk) for the risk of a Type I error (α-risk). Where statistical

significance determines if there is a difference between two groups, effect size quantifies the difference

between two groups. Bigger effects are easier to detect than smaller effects. If the data being sampled

has a large amount of variance, both from the value being measured and the noise in the data, this will

decrease the statistical power. [2] Measurement error is also a source of noise. The goal of using DNA

Barcoding to resolve taxa in more detail to the genus and species level, is to reduce variability and

therefore increase statistical power. Increasing the precision of the measurement increases the statistical

power and/or decreases sample size. A statistical power of 0.80 is typical, and indicates a 4:1 trade off

between β-risk and α-risk. Highly consistent systems in engineering and physical sciences, as well as

medical tests where the risk of a false negative (not detecting a disease) can have higher statistical power

such as 0.90.

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DNA Barcoding increases resolution from family level, to genus and species, as well as reducing

error from manual taxonomic identification by morphology. In the case of Chironomidae this means that

genus level tolerance values ranging from 0 to 10 can be used instead of the family level tolerance value

of 6. This increases the statistical power of the bioassessment method.

5. Conclusions :

5.1 Based on Bland-Altman analysis waterway ecosystem bioassessment by DNA Barcoding of

Chironomidae is sensitive enough to be a viable option for bioassessment globally. Manual taxonomic

identification under magnification is typically only performed to the family level. Stream health data

from Chironomidae genera matched historical health data. (Statistically significant p



to databases used by the scientific community. Phylogenetic tree groupings match geography and

historical health data. Samples from the healthiest sites are nearly genetically identical. The most

sensitive genus of Chironomid was only found in the healthiest sites.

5.5 DNA Barcoding of Chironomidae can be faster and lower cost than the current method. This method

is robust, reproducible, and suitable for augmenting citizen science initiatives.

5.6 In analyzing the distribution of Chironomidae genera between streams with urban vs. open space

catchment areas, there was not a statistical correlation. This may require further study with more detailed

land use data. (Not statistically significant p>.05)

5.7 Finally, the investigation into the Chironomidae family shows that DNA Barcode analysis can result

in waterway health data that is both more accurate and more precise, and therefore increase statistical

power and significant value for monitoring an increasingly scarce water resource.

6. References: [1] Bland, J. Martin, and Douglas G. Altman (2010). Statistical Methods for Assessing Agreement between Two Methods of Clinical Measurement. International Journal of Nursing Studies, vol. 47, no. 8, 931–936. [2] Coe, Robert (2002). It's the Effect Size, Stupid: What Effect Size Is and Why It Is Important. University of Leeds, Education-Line, www.leeds.ac.uk/educol/documents/00002182.htm. [3] “Competing for Clean Water Has Led to a Crisis: Clean Water Crisis Facts and Information”, National Geographic, 27 Jan. 2017 [4] Epler, John H. (2001). Identification Manual for the Larval Chironomidae (Diptera) of North and South Carolina. EPA Region 4 and Human Health and Ecological Criteria Division [5] GIS waterway and World Light Gray Reference, (2019) Esri Data & Maps [6] “The Global Risks 2015 Report”, World Economic Forum, 2015 [7] Hilsenhoff, William L. (1977), Use of Arthropods to Evaluate Water Quality of Streams. Wisconsin Department of Natural Resources, Technical Bulletin No. 100, Madison, WI [8] Land Acquisition, www1.nyc.gov/html/dep/html/watershed_protection/land_acquisition.shtml, 2018 [9] NJ Division of Water Monitoring and Standards. http://www.nj.gov/dep/wms/, 2018 [10] Public Supply Water Use, www.usgs.gov/special-topic/water-science-school/science/ public-supply-water-use?qt-science_center_objects=0#qt-science_center_objects, 2018 [11] Rueb, Emily S. “How New York Gets Its Water”, New York Times (New York, NY), 24 Mar. 2016 [12] Salazar, Cristian. “How Does New York City Get Its Water?” Am New York, (New York, NY) www.amny.com/lifestyle/how-nyc-gets-its-water-1.9205765, 18 April 2018 [13] “Scarcity.” UN-Water, www.unwater.org/water-facts/scarcity/, 2018 [14] “Water Scarcity.” WWF, World Wildlife Fund, www.worldwildlife.org/threats/water-scarcity, 2018 [15] Stein, E. D., White, B. P., Mazor, R. D., Jackson, J. K., Battle, J. M., Miller, P. E.,. Sweeney, B. W. (2014). Does DNA barcoding improve performance of traditional stream bioassessment metrics? Freshwater Science.

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7. Bibliography Cañedo-Argüelles, Miguel, et al. (2016). Are Chironomidae (Diptera) Good Indicators of Water Scarcity? Dryland Streams as a Case Study. Ecological Indicators, vol. 71, 2016, 155–162. Carew, M. E., Pettigrove, V. J., Metzeling, L., & Hoffmann, A. A. (2013). Environmental monitoring using next generation sequencing: rapid identification of macroinvertebrate bioindicator species. Frontiers in Zoology. Ekrem, Torbjørn, et al. (2010). Females Do Count: Documenting Chironomidae (Diptera) Species Diversity Using DNA Barcoding. Organisms Diversity & Evolution, vol. 10, no. 5, 2010, 397–408 Ekrem, Torbjørn, et al. (2018). DNA Barcode Data Reveal Biogeographic Trends in Arctic Non-Biting Midges. Genome, vol. 61, no. 11, 787–796. Folmer, Ole & Black, Michael & Wr, Hoeh & Lutz, R & Vrijenhoek, Robert. (1994). DNA primers for amplification of mitochondrial Cytochrome C oxidase subunit I from diverse metazoan invertebrates. Molecular marine biology and biotechnology. 294-9. Hilsenhoff, William L. (1982). Using a Biotic Index to Evaluate Water Quality in Streams. Wisconsin Department of Natural Resources, Technical Bulletin No. 132, Madison, WI. Lin, Xiao-Long, et al. (2018). DNA Barcodes and Morphology Reveal Unrecognized Species in Chironomidae (Diptera). Insect Systematics & Evolution, vol. 49, no. 4, 2018, 329–398. MacCafferty, W. P. (1981). Aquatic Entomology. Jones and Bartlett. Sudbury, MA. Merritt, R. W. (1984). An introduction to the aquatic insects of North America. Kendall Hunt, Dubuque, IA. Micklos, D. A. (2003). DNA SCIENCE: A First Course. Cold Spring Harbor Laboratory Press, Cold Spring Harbor, NY. Micklos, D. A., Nash, B., Hilgert, U. (2013). GENOME SCIENCE: A Practical and Conceptual Introduction to Molecular Genetic Analysis in Eukaryotes. Cold Spring Harbor Laboratory Press, Cold Spring Harbor, NY. Pilgrim, E. M., Jackson, S. A., Swenson, S., Turcsanyi, I., Friedman, E., Weigt, L., & Bagley, M. J. (2011). Incorporation of DNA barcoding into a large-scale biomonitoring program: opportunities and pitfalls. Journal of the North American Benthological Society, 30(1), 217-231. Silva, Fabio & Ekrem, Torbjorn & Fonseca-Gessner, Alaide. (2013). DNA barcodes for species delimitation in Chironomidae (Diptera): A case study on the genus Labrundinia. The Canadian Entomologist. 145. Singh, P., Rawal, D. (2016). Molecular phylogeny of Einfeldia (Diptera: Chironomidae) inferred from sequencing of mitochondrial cytochrome oxidase subunit 1 (COX1) gene, International Journal of Entomology Research, Volume 1; Issue 6; 11-15 “Volunteer Stream Monitoring: A Methods Manual”, United States Environmental Protection Agency, https://nepis.epa.gov/Exe/ZyPDF.cgi/P100MRC3.PDF?Dockey=P100MRC3.PDF, (2018). Walton, Brett, and Brett Walton. “Cape Town's Water Panic Was Years in the Making.” CityLab, 17 July 2018, www.citylab.com/environment/2018/07/how-cape-town-got-to-the-brink-of-water-catastrophe/564800/. Images credited to author unless otherwise noted. Original artwork by author

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